Methods and hosts for rearing insect parasitoids are provided. Particularly, polymer beads (alginate, carrageenan, and chitosan) are used to rear endoparasitoids in vitro.
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1. A method of rearing an endoparasitoid comprising: rearing the endoparasitoid in a spherical biopolymer bead or capsule, whereby the bead or capsule acts as a host for the endoparasitoid.
15. A method for continuous in vitro rearing of an endoparasitoid comprising the steps of:
laying an egg of an endoparasitoid in a spherical biopolymer bead or capsule which comprises a nutritive solution, and
maintaining said bead or capsule in an oxygenated sterilized nutritive solution during endoparasitoid development.
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12. The method for rearing an endoparasitoid according to
13. The method for rearing of an endoparasitoid according to
14. A system for rearing endoparasitoids comprising:
at least one bead or capsule as defined in
at least one endoparasitoid, and
an environment suitable for oviposition of said endoparasitoid on said bead or capsule.
16. A method according to
17. A biopolymer bead or capsule comprising an embed mummy of an endoparasitoid obtainable by the method of
18. A method of treating a pest which comprises administering the biopolymer bead or capsule of
19. A method for mass production of large amounts of endoparasitoids comprising pulverization of biopolymer beads or capsules obtainable by the method of
20. A method according to
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This is the U.S. National Phase under 35 U.S.C. §371 of International Application PCT/EP02/06936, filed Jun. 21, 2002, which claims priority of EP 01870134.2, filed Jun. 22, 2001 Each of the above applications are incorporated herein by reference in their entirety.
The present invention relates to the field of insect pest control using biocontrol agents. The invention relates to the use of polymer beads (alginate, carrageenan, chitosan) or capsules to rear endoparasitoids of insects in vitro.
The principal method of controlling pests, such as aphids, throughout the world is that of treating the infested crop with insecticides. However, there are drawbacks to this method such as environmental pollution, harmfulness for humans and animals, increased resistance in key pests, creation of secondary pest outbreaks, effective elimination of beneficial insects and so forth. Nowadays, there is an increasing interest in reducing the use of pesticides.
An alternative to chemical pesticides is the use of biocontrol agents such as predaceous and parasitoids for controlling insect pests. Nevertheless, millions of these beneficial insects, so-called biocontrol agents, are required for using this method in the fields. At the present time, for the mass production, it is still necessary to rear these insects on their natural hosts, for instance cereal aphids. This classical method is too expensive to allow large-scale use of beneficial insects in commercial agriculture. A solution seems to be the development of artificial media to rear these beneficial insects. Indeed, this method will allow reducing the cost of the mass production.
Since many years, the researchers develop methods to raise the beneficial insects (predators and parasitoids) on artificial media. Simmonds (1966) attempted to culture three ectoparasitic ichneumonids of coding moth pupae on nutritive gelatine slants and raw beef. Yazgan (1972) and House (1978) used a dietetic approach to prepare media utilizing existing knowledge of the nutritional requirements of insects generally, to successfully rear the parasitic hymenopteran Itoplectis conquisitor (Say) in chemically defined, synthetic diet. House (1978) encapsulated a synthetic diet within a Parafilm RTM capsule and created an artificial host that also served adequately for oviposition and rearing for I. conquisitor. Hoffman and Ignoffo (1974) and Hoffman et al., (1975) developed media that allowed at least partial success in rearing the pupal endoparasitoid, Pteromalus puparum (L.) and the egg parasitoid Trichogramma pretiosum (Riley), respectively.
Grenier et al. (1994) presented a review of over a half century of research on development of artificial media for entomophages, and report successes in producing media for ectoparasitoids and predators but not for endoparasitoids. Curiously, none of these artificial media has found its way into use in the commercial production of any entomophage, and none of these media have been incorporated into the augmentative production systems for these predators.
In order to fight against aphids, the most important pest insects in the agriculture of the temperate climatic zones, endoparasitoids are often effective biological control agents. Nevertheless, the number of parasitoids in the crops are often too low to reduce strongly the aphid populations. Thus, inundate releases of these beneficial insects are essential. Unfortunately, at the present time no artificial medium to rear these endoparasitoids was developed.
Despite considerable effort, no hymenopterous larval endoparasitoid has been successfully reared from egg to adult in artificial media. However, partial success has been attained with two braconid larval endoparasitoids, Microplitis croceipes. (Cresson) and Cardiochiles nigriceps (Viereck), and one braconid larval-pupal endoparasitoid, Diachasmimorpha longicaudata (Ashmead). Pennachio et al. (1992) have cultured the Heliothis virescens braconid larval endoparasitoid Cardiochiles nigriceps from post-germband eggs to the second instar in an artificial medium comprised of an amino acid, salt, vitamin, and carbohydrate-containing medium supplemented with bovine serum albumin, enzymatically hydrolysed lactalbumin, fetal bovine serum, egg yolk and milk. However, the larvae grew much slower than in vivo, only 10% moulted to the second instar and they did not complete development.
It is an aim of the present invention to provide methods and artificial hosts for continuous rearing endoparasitoids.
It is also an aim of the present invention to provide artificial hosts for oviposition of endoparasitoids.
It is a further aim of the invention to provide methods for producing artificial hosts for endoparasitoids.
It is also an aim of the invention to provide a means for storage of artificial hosts containing endoparasitoids and to apply them easily where they are needed for biological control programs.
Until the present invention, eggs and larvae of hymenopterous endoparasitoid were collected from previously parasitized hosts, sterilised and were immersed in the nutritive solution in vitro. Nevertheless, these handlings could wound the parasitoids, are very time consuming and do not allow actual mass rearing. The invention now provides new hosts for endoparasitoids.
The use of biopolymer beads or capsules as host or recipient for oviposition makes its possible to avoid all handling, for instance by continuously furnish the necessary nutrients by bringing the beads or capsules (after oviposition) into a nutritive and oxygenated solution which allows diffusion through the polymer matrix without removing the media inside the beads. Beads or capsules containing the nutritive solution may be produced in large quantity at low cost and stored for a long time in sterile conditions without loosing their properties before to be used for endoparasitoid production.
The use of biopolymer beads or capsules as hosts or recipient for oviposition makes it possible to avoid all these handlings.
Polymer beads such as alginate and chitosan are used in a variety of areas of biotechnology in encapsulation processes. These beads are used to encapsulate various materials such as enzymes, hormones; drugs, adsorbents and so forth. The viable biomaterials to be encapsulated can also be tissue, organelle, plant or animal cells, bacteria, algae, fungi and so forth. The material must be of a size small enough to be suitable for encapsulation by the droplet method of this invention but can vary widely in diameter from less than a micron to several millimetres.
It is embodied in the present invention to use these polymer beads or capsules to rear endoparasitoids of insects. These beads or capsules would contain a nutritive solution for these endoparasitoids and be coated by substances enhancing oviposition such as epicuticular host (aphid) or other host's compounds and/or of plant extracts. The parasitoid would lay an egg in the beads or capsules with its ovipositor and the larva fed by the nutritive solution would develop in the bead. The beads or capsules may be brought into a continuous flow of sterilized and oxygenated nutritive solution. Indeed as parasitoid larvae in development will consume the nutrient and oxygen present in the nutritive solution, it may be necessary to provide continuously new nutrients. This is possible because of the use of hydrophilic biopolymers which are a matrix containing pores allowing the diffusion of big molecules such as BSA (69 kDa). At the end of the development of the third stage larvae, beads or capsules will be removed, preferably automatically, from the nutritive media and placed in a constant temperature chamber with a relative humidity ranging from 75% to saturation. The larva would then spin a cocoon and after some days, adults would emerge from the beads or capsules. The methods provided by the present invention may reduce considerably the time needed for in vitro rearing as it reduces the hand manipulating needs to nearly nothings, avoiding the risk of damaging the endoparasitoid during its development and allowing industrial automated mass rearing. Concerning the mass release in agricultural field or in every place or time needed for biological control of insect pest by endoparasitoid, the said system will even allow for instance the spraying of a large amount of embedded mummies placed in an adequate solution such as a salt physiological solution (NaCl, 0.07% buffered at a pH ranging from 6 to 7.5) and spraying using a classical pulverisator as currently used by farmers. So, it may represent an ideal system for mass biological control program from the endoparasitoid production to their mass released where needed.
The nutritive medium in order to rear endoparasitoids is a nutritive solution comprising sucrose, amino acids, vitamins, mineral salts and sterols encapsulated in a spherical biopolymer bead or capsule. Preferably, said liquid nutritive solution comprises at least one of the following essential compounds: Trehalose (concentration may range from at least 10 mg to 1 g/100 ml), cholesterol (ranging from at least 10 to 100 mg/100 ml) or other sterols, FBS (fetal bovine serum, at least 1 to 20% v/v) and vitamin C. The pH of the media may range between 6 and 7.5. The polymer used may be an alginate, a carrageenan or a chitosan (and mix of two polymers). Other hydrophilic biopolymers could also be used.
The medium may be encapsulated during the preparation of the beads or capsules and/or may be introduced by diffusion by immersing the beads or capsules in the nutritive solution after their manufacture.
The same nutritive solution may also be used to bring in the beads and the capsules. This medium may be oxygenated and sterilized. For instance, the beads or capsules are placed in a device looking like a fermentor, alimented by a flow of oxygenated and sterilized medium.
According to a first embodiment the present invention relates to the use of a polymer or hydrogel bead or capsule as a host for an endoparasitoid.
The term “polymer” or “hydrogel” as herein used are interchangeable and merely relate to the method of manufacture in that a hydrogel is a gel prepared in an aqueous solvent whereas a polymer is a large molecule which is generally built from smaller units or monomers. Preferred are biopolymer beads or capsules.
The term □endoparasitoid□ relates to an insect and especially a wasp that completes its larval development within the body of another insect eventually killing it and is free-living as an adult.
According to a further embodiment, the invention relates to the use of polymer beads or capsules for in vitro rearing of endoparasitoids wherein said beads or capsules are used for oviposition.
The term “oviposition” relates to the laying of eggs by means of an ovipositor, for instance by insects. The term “ovipositor” relates to an organ or set of organs at the end of the abdomen, by which eggs are deposited. According to the present invention, the endoparasitoid will deposit one or several eggs in the polymer bead or capsule.
The term “capsule” relates to a hollow bead composed from a combination of components, further characterised in that during the manufacture of said capsules, a thickener, preferably dextran or lambda carrageenan has been added to the salt solution.
The polymer beads or capsules may be composed of alginate, carrageenan or chitosan. These biopolymers are also chosen because they are natural, non-toxic products which are completely biodegradable and safe for the environment.
Several examples of polymer beads or capsules, composed of one of said components or composed of mixtures of at least two of said components are described in the examples sections.
In the prior art, several methods have been described to prepare polymer beads or capsules. However, in the present invention are described methods for the preparation of polymer beads or capsules which are especially suited for use in methods for rearing insect parasitoids. The preparation of beads or capsules is a modification from protocols described in the literature (Wrong and Somesh, 1995; Velings, 1997; Somesh et al., 1988). The basic protocol used for the preparation of the biopolymer capsules is described in Somesh et al.
However, the capsules prepared using these conditions, did not always result in the deposition of eggs and also the shape of the capsule was highly variable. For instance, when capsules are used, in order to allow oviposition, the thickness of the wall would preferably range between 5 and 100 μm. This is one reason why the literature protocols for preparing capsules had to be modified to produce biopolymers suitable for use in the embodiments of the present invention.
According to another embodiment the invention thus also relates to a method for preparing hydrophilic and porous biopolymer capsules for in vitro rearing of endoparasitoids comprising:
With respect of the preparation of the capsules, the modifications concern the concentration of chitosan, the concentration of the ionic solution and the duration of the stay in the chitosan solution which are necessary to provide the beads with the required characteristics and properties.
The duration time in the chitosan (polymer) solution is needed to ensure the formation of the required size of beads or capsule, a correct sphericity and a good repeatability of the beads or capsule formation. For the chitosan capsules, the time the beads are kept in the polymer solution also determines the thickness of the wall of the capsule. If the wall of the capsules is too thick (more than 100 micron), the endoparasitoid is not able to pierce it to lay an egg, as the size of its ovipositor is approximately 100 microns. If the wall of the capsule it is not thick enough, then the capsule will collapse during manipulation. Preferably the size must be between 5 to 10 and 100 microns, most preferably the wall is between 20 and 40 μm, 10 and 50 μm, between 10 and 60 μm, between 10 and 80 μm, or between 30 and 70, or the wall thickness is 25 μm or 35 μm.
The concentration of polyphosphate anions will determine the number of interactions (and their strength) between the chains of polymer (Chitosan) and thus the thickness of the wall. The wall thickness may be measured using an optical microscope or an electronic microscope. The optical microscope is recorded through a camera to a computer, which in function of the magnification used calculates the real thickness. Also other techniques can be used for measuring wall thickness which are well known by the skilled in the art, for instance NMR spectroscopy.
Further, if the maturation time (the time the beads or capsules are treated with pentasodium tri-polyphosphate, is too long (for instance 30 minutes or longer) several layers are observed in the wall of the capsule, and the thickness of the wall being not homogenous for the whole of the capsule area.
Further, agitation of the solutions (e.g. the polymer solution wherein the ionic solution is dropped for preparing the capsules or the pentasodium tri-polyphosphate solution wherein the polymer solution is dropped in case of preparing beads) is needed to ensure a homogenous shape of the capsule,
An optimized % of chitosan (preferably between 1 and 0.5%, more preferably 0.75%), % of pentasodium tri-polyphosphate (preferably between 1.5 and 3.5%, more preferably 2.5 or 3%), and optimised pH (pH of the polymer solution obligatory lower than 5.5, preferably 3.5, the pH of the ionic solution may be between 6 and 9, and preferably 7 or 8) are needed to obtain stable capsules with a good sphericity and elasticity to allow the introduction of the ovipositor. If the capsule is too resistant, the parasitoid is not able to lay an egg inside. These conditions are also the better ones to allow a correct porosity and diffusion of the nutrient inside the capsule.
A yellow pigment is added to the capsule, it may be STABILOBOSS™ yellow or any other yellow organic pigment such as lutein. Preferably the beads or capsules are colored by diffusing by adding said pigment at low concentrations, for instance between 1 and 10%, preferably 4 or 5%. An example of the increase in attractivity of yellow pigment is given in Table 1. As such, the invention also relates to biopolymer beads or capsules obtainable by any of the methods described herein and which methods provide the beads or capsules with essential properties for use in rearing endoparasitoids.
As such, the invention also relates to polymer beads or capsules obtainable by any of the methods described herein because these beads or capsules have now the required features that make them suitable for the use of the present invention.
Furthermore, the polymer beads or capsules prepared by any of these methods can be filled with a nutritive solution whereon the larvae can feed when developing from the egg.
Therefore, the present invention more particularly relates to polymer beads or capsules comprising an outer wall composed of a polymer, preferably a biopolymer and more preferable made from alginate, carrageenan, chitosan or a mixture thereof. Said outer wall may consist of one or more layers. The outer wall of the bead or the capsule must have a thickness which is sufficient but not too large to enable the endoparasitoid to enter its ovipositor in it. Further the bead or capsule needs to be hydrophilic and to have a porosity, which allows the entrance of a nutritive solution by diffusion.
Another important feature of the polymer beads or capsules to be suitable for the uses herein described is the diameter of the bead or capsule. Preferably the diameter of the beads or capsules is of approximately the same size as their host. Preferable the diameter of the beads or capsules ranges between 1 and 5 mm, more preferably between 1.5 and 3 mm.
The size of the bead is influenced by the method of preparation. The diameter of the needle determines the size of the drops that fall in the solution and thus determines the size of the capsules or beads. The size is chosen to obtain the best value allowing the manipulation of the beads or capsules by the endoparasitoid prior or during oviposition (antennae contact, walk on the beads or capsules, insertion of the ovipositor). The horizontal position (see
Further, the drop rate must be as high as possible to reduce the duration of time between the moment at which the first drop touches the liquid surface (polymer or ionic solution) and the moment at which the last one enters in contact with the liquid. This is important to avoid a too important difference of stay time in the solution. However the drop rate cannot be too high to avoid obtaining a continuous flow instead of drops.
The viscosity of the drop must be sufficiently high to conserve a spherical shape during the fall and at the moment when the drop enters the solution. If viscosity is too low, than the drop crashes on the liquid surface and flatten or disaggregates in the solution. If viscosity is too high, the liquid moves with difficulty in the tubes and needle of the device. The viscosity is determined by the dextran concentration (Molecular Weight MW). The viscosity thus determines the dextran concentration used.
Preferably, inside the bead or capsule, a cavity is present wherein an egg can be deposited, preferably by an endoparasitoid. It should be clear that eggs or larvae can also be deposited inside these beads, for instance by micro-injection.
Preferably, the said inner cavity is filled with a nutritive solution that allows the hatching of the eggs and the development of the larvae. Said polymer beads or capsules are extremely suited for use as host for endoparasitoids as they allow the passage of oxygen and carbonic gas but also of large range of molecules including Bovine serum albumin (69.000 daltons) because of their hydrophilic nature and the porous matrix they constituted by polymerisation. As the endoparasitoid larva consumes nutrients during its development, beads or capsules may be immersed in the nutritive solution, constantly oxygenated and sterilized using a flow system and a fermentor-like device. Nutrients and oxygen may then diffuse through the beads or capsules' walls to aliment the larva, without any manipulation of the said larva or removal or change of the initial nutritive solution in the bead or capsule.
When preparing the capsules or beads, there are several possibilities to introduce the nutritive media inside. A first option is to immerse the capsules or beads after preparation in the nutritive solution and let nutrients enter by diffusion. The second option is during preparation, for instance of the capsules, to mix the nutritive solution with the dextran and the tripolyphospahte (ionic solution). Then a droplet of that liquid is dropped in the chitosan solution that polymerizes at the surface of the droplet to produce a capsule. The tri-polyphosphate provokes the polymerization, the dextran is used to thicken the solution. In that condition, the solution is trapped inside the capsule during polymerization. In the Examples section such an encapsulation procedure is described.
Preferred nutritive solution contain sucrose, trehalose, aminoacids, vitamins, mineral salts and sterols in defined conditions. Essential compounds that have to be present are: Trehalose (concentration ranging from at least 10 mg to 1 g/100 ml), cholesterol (ranging from at least 10 to 100 mg/100 ml) or other sterols, FBS (fetal bovine serum, from 1 to 20% v/v), vitamin C and choline. Mineral salts are Na2HPO4, MgSO4 and CACL2. The pH of the media may range between 6 and 7.5. One example of such a nutrient solution, for instance to rear Aphidius rhopalosiphi larvae is described in Table 4.
In order to enhance oviposition, beads or capsules may be coated by epicuticular host extracts (such as squalen or octadecyle hexadodecanoate or other alcane, alcene, ester and aldehyde compounds, Table 6 shows some examples), host pheromones such as B-farnesne and/or plant extract. Trehalose has to be present inside the beads or capsules (in concentrations ranging from at least 10 mg to 1 g/100 ml) to increase oviposition. Moreover, capsules or beads are colored in yellow preferably using Stabilo marker ® as yellow colorant. These colored beads or capsules are more stimulating for endoparasitoid and are preferably attacked with regards to their normal host (see
In the present invention it is demonstrated that a combination of the biopolymer capsules or beads as described and as prepared by the modified methods, and the yellow colour induce a true oviposition response including the egg laying, and not just an oviposition attack that which does not mean that an egg is really deposited. Indeed, endoparasitoid possess on their ovipositor, nervous sensillae allowing them to probe and to evaluate the host before laying eggs.
The invention thus relates to the use of a polymer bead or capsule as described above as a host for endoparasitoids. In a related embodiment the invention relates to the use of said polymer or hydrogel beads for in vitro rearing of endoparasitoids.
According to a further embodiment the invention relates to the use of polymer beads or capsules for continuous or step by step in vitro rearing of endoparasitoids.
According to a more specific embodiment the invention relates to the use of said biopolymer bead or capsule is used for oviposition and continuous rearing of an endoparasitoid from the egg through to the adult emergence of said endoparasitoid
The expression “continuous rearing” or “continuous in vitro rearing” as used herein is marked by a sequence of the developmental stages involving the development of an endoparasitoid from the egg stage to the stage of embedded mummy or adult emergence, without any external manipulation. This is possible by the use of the beads or capsules of the invention which allow all these stages to proceed within the bead or capsule itself, without any manual handling or manipulation of the beads or capsules. Optionally one external manipulation, which is also part of the present invention, is performed i.e. the storage of embedded mummies at low temperatures and high humidity for a further application.
The expression “step by step rearing” as used herein relates to the method of rearing endoparasitoids in a discontinuous way, essentially rearing the endoparasitoids according to the same methods of the continuous way but leaving the possibility of collecting the endoparasitoids at any stage (step) of development and keeping them in a quiescent stage for a defined period of time before re-entering them in the further developmental stage. Since the beads or capsules are nearly transparent, it can easily be monitored in which developmental stage is the endoparasitoid in the bead.
Other moments or stages in the development of the endoparasitoid wherein the development of the endoparasitoid can be rested are for instance the larval stages 1, i.e. just after the egg hatching, 4 to 5 days after oviposition. At that stage, larvae 1, development can be interrupted for several days (2 to 5) by placing them at 5° C. in a nutritive solution.
The Embedded Mummy
According to yet another related embodiment the invention relates to the use of said beads for oviposition, preferably for oviposition of hymenopterous endoparasitoids or insects.
According to a preferred embodiment the invention especially relates to the use of polymer beads or capsules as a host for endoparasitoids which beads or capsules are hydrophilic and porous, for instance biopolymer beads or capsules which are at least partly composed of alginate, carrageenan or chitosan, or mixtures thereof.
According to a more specific embodiment the invention relates to the use of biopolymer beads which are essentially composed of alginate wherein said alginate is a copolymer of beta-D-mannuronic acid and alpha-L-glucuronic acid, cross-linked by divalent cations, such as Ca++ ions.
The term “at least partly” as used herein means from about 10% to almost 100%, for instance 20%, 30%, 40%, 50%, 60%, 70%, 80%, 90%, 95% or 99%.
The term “essentially” as herein used means that about 80 to 100% of its composition is alginate.
According to a preferred embodiment the invention relates to the use of polymer beads or capsules that are also essentially composed of Chitosan as a host for endoparasitoid wherein said chitosan is a derivative of chitin (poly-beta-(1-4)-2-amino-2-deoxy-D-glucopyranose) found in a large number of species of fungi, crustacea, insects and other Arthropods. As chitosan is the major component of insect cuticle, it is thus particularly well recognized by the endoparasitoid during oviposition and well suited for their development. The porous nature of the polymer matrix also allows the insect to perceive the inner composition of the media by antennal contact before oviposition.
The beads or capsules of the present invention can be used as a host for in vitro rearing of endoparasitoids, preferably hymenopterous endoparasitoids belonging to the order of insects (Hymenoptera).
Preferred endoparasitoids which are envisaged in the present invention to be reared using artificial hosts as described above, are chosen from the list of aphid endoparasitoids presented in Table 5.
Nevertheless, it should be clear that the present invention is not limited to rear aphid endoparasitoids but can also be used for other endoparasitoids.
It has been shown by the present inventors that additional stimuli can augment the success of oviposition by the endoparasitoids.
Therefore, the invention further relates to a method for in vitro rearing of endoparasitoids comprising the use of polymer beads or capsules as described or obtainable by any of the methods herein disclosed for oviposition wherein said endoparasitoids are placed in environment comprising wheat and/or their natural hosts. According to a further alternative the endoparasitoids are placed in an environment comprising wheat or parts of a plant, or plant odours and/or their natural hosts or the odours of these natural hosts.
Preferably when for instance hymenopterous endoparasitoids are to be reared when using polymer beads or capsules, the endoparasitoids are placed in an environment comprising wheat and cereal aphids. According to a further alternative the endoparasitoids are placed in an environment comprising wheat and cereal aphids or the odours of cereal aphids.
The beads or capsules themselves however may imitate the texture, the odor, the color and other characteristics or properties necessary for oviposition. As illustrated in the examples the colour of the bead or capsule may have a positive influence on oviposition. Therefore, according to a preferred embodiment, the polymer beads or capsules for use as a host for rearing endoparasitoids are yellow, preferably coloured yellow with STABILOBOSS™ yellow.
According to another embodiment, the invention also relates to the use of the polymer beads or capsules as described herein wherein said beads or capsules are coated with host epicuticular extract and/or plant extract.
The present invention further relates to any of the uses as described wherein said endoparasitoid is chosen from the group of hymenopterous endoparasitoids as listed in Table 5.
The invention further relates to a method for in vitro rearing (e.g. continuous) of an endoparasitoid comprising the steps of:
Using the above method, the endoparasitoids may be continuously reared until the desired stage of development.
The invention thus relates to a method for rearing for in vitro rearing endoparasitoids until the stage of embed mummies comprising the step of collecting the bead or capsule when the endoparasitoid is an embedded mummy.
The invention also relates to a biopolymer bead or capsule comprising an embedded mummy of an endoparasitoid obtainable by the above described method.
To allow their survival and commercial distribution, it is important that these mummies are stored in a solution. The nutritive solution is a possibility but probably to expensive if it is only needed for distribution because during metamorphose parasitoids will not need nutrients. Water alone is not sufficient because of the osmotic pressure, the parasitoid mummies is hypertonic and so water will enter the bead and the mummy and will provoke damages to the endoparasitoids' cells by increasing the inner pressure. Therefore a more favourable way is to use a salt isotonic solution (for instance 0.007% NaCl buffered at a pH ranging from 6 to 7.5) or any other solution that has the same effect on the mummy and that can be used to preserve living tissues. So the final product may be the embedded mummy (mummies) in an isotonic salt solution. The farmer just needs to pulverize (e.g. disperse or spray) the solution. The release of a great quantity of parasitoids in a field, for instance a wheat field of several ha, in order that these parasitoids may be distributed evenly is a very difficult task. The present invention provides a concentrated amount of beads or capsules comprising the embedded mummies in a preservative solution which may be diluted according to the needs of the farmer or the machines he uses. The present invention thus allows just to spray (pulverize) the embedded mummies like an insecticide, using the classical systems (pulverisator; diffusers) every farmer or plant producer (horticulturist, gardener, etc.) has in his farm or company. The capsules or beads present in the solution will be dispersed evenly on the plants in the field and will dry just because the outdoor air is not saturated in water. When drying the biopolymer becomes sticky and will remain on the plant until the emergence of the parasitoid even if there is wind or rainfall. Under these conditions, on the plant the survival of the parasitoid before emergence will be better than just on the soil.
The term “pulverization” as used herein means spraying the solution containing the beads or capsules to allow their dispersion in the field, like an insecticide. A pneumatic system of pulverization or application may also be used to propel the beads or the capsules containing the mummies.
The invention also relates to a method for rearing for in vitro rearing endoparasitoids until the stage of adult emergence comprising the step of collecting the endoparasitoid when emerged from the bead or capsule.
The invention also relates to an endoparasitoid obtainable by (e.g. reared by) the methods described herein.
The invention further relates to the use of biopolymer bead or capsule or an endoparasitoid obtained by or obtainable by any of the methods of the invention for mass release in pest control.
According to another embodiment, the present invention relates to method for mass production of large amounts of endoparasitoids comprising pulverization of biopolymer beads or capsules obtainable by the methods herein described by placing said beads or capsules in an adequate solution and/or pulverization using a pulverisator
Furthermore the invention provides a system for rearing endoparasitoids comprising:
Said system may comprise at least one of the following:
The term “embedded mummy” relates to the pupal stage (last developmental stage during which metamorphosis takes placed) of the endoparasitoid embedded inside the capsule or the bead in which it has spun a cocoon, before emergence of the adult. The pupae stage is very easy to visually recognize just by a glance, as just before pupation, the larval stage 3 endoparasitoids eject content of the digestive tract, what is call meconium. The meconium is very easy to see as it forms a small dark spot. As capsules and beads are nearly transparent, a dark spot is easy to identify just by a rapid check during production. For instance, when it is noted that most beads or capsules contain stage 3 larvae, the beads may be collected manually from the nutritive solution, or automatically, for instance by giving an apparatus an instruction (e.g., turning a knob or computer guided instructions) that the container comprising the beads or capsules and nutritive solution is emptied and beads or capsules are for instance filtered and transferred or transported to a following compartment or container where the next stage in development can proceed.
The rear chamber will receive the capsules or beads containing larval stage 3 at the end of its development to allow metamorphosis. Indeed at that moment for metamorphosis, full-developed Larva 3 do not eat anymore, and so do not need to be immersed in a nutritive solution. Metamorphosis is done using its fat and glycogen reserves. If the beads or capsules would remain in the nutritive solution at that stage of parasitoid development, the adult would be incapable to leave the capsules and will drown itself in the solution. In this respect, this step participates to the continuous rearing process.
The cold chamber is used to store the capsules or beads at the right temperature. Our experiments have shown that it is possible to store embedded mummies at about 3° C. under high humidity (e.g. from 70 to 100%), preferably under intermediate humidity (from 80 to 97%) at least for 3 to 5 weeks in quiescence stage, and possible longer for several months (1 to 6) in a diapause stage. It is likely to avoid saturated air to prevent the growth of fungi, which do not become visible in cold storage, but develop on the mummies when they are back at normal temperatures for development (e.g. 20° C.).
The term “quiescence” relates to the response of individual insects to a sudden unanticipated, non-cyclic and usually short deviation from normal weather conditions. As used herein, “quiescence” relates to a metabolic rest which can be induced by low temperature i.e. under the development threshold of the insect, currently about 6° C. but may depend on the parasitoid used. As soon as temperature increase over for instance 6° C. in the above case, the development goes on.
The term “diapause” relates to a hormonally-mediated state of low metabolic activity, associated with reduced morphogenesis, increased resistance to environmental extremes and altered or reduced behavioral activity. Diapause occurs during a genetically determined stage of development (e.g. at the pupal stage) in response to environmental cues (currently a reduction of the day duration like in autumn) that precedes unfavorable conditions (such as Winter). As used herein “diapause” relates to a metabolic rest that can be induced by low enlightenment duration mimicking weather conditions of autumn. At that stage the endoparasitoid remains alive during 3 to 6 month at low temperature.
The present system thus provides for several options, for instance the possibility of (1) only a rear chamber until the endoparasitoid emerges from the mummy, (e.g. collection of endoparasitoids), or (2) a rear chamber until the endoparasitoid is an embedded mummy and then transferred to a cold chamber for storage, (e.g. collection of beads with embed mummies). Other options provide for the collection of any other developmental stage of the endoparasitoid whenever there is a need thereof.
The system thus directly provides a means of producing parasitoids or beneficial insects at large scale. The said produced endoparasitoids or their embedded mummies, directly after production or storage, may be used for mass releases in the frame of biological control of insect pests. These releases may be done by hand or by any kind of dispersal devices. Embedded mummies may be placed in an adequate solution such as a salt physiological solution (NaCl, 0.07% buffered at a pH ranging from 6 to 7.5) and pulverized using a classical pulverisator. As when they dry, the said biopolymer constituting the bead or capsule become sticky, the embedded mummies will stick on the plant in good conditions before adult emergence. A pneumatic system of pulverization or application may also be used to propel the beads or the capsules containing the mummies. Both systems will allow a homogenous dispersal of the endoparasitoids where needed. They do not exclude the possible use of a slow release system like a diffuser system containing the said beads or capsules.
As used herein, the term “diffuser” relates to a device that allows to release slowly a certain amount of parasitoid per unit of time. It could be a box where the parasitoid or embedded mummies are stored with some food for the adult and that will allow the adults to meet inside after emergence and possibly to mate. It could be any other kind of device that will be placed in the fields, orchards or glasshouses allowing the emergence of adults and their release. It is an alternative to a spraying device or any kind of dispersal device.
The term “environment” in this aspect can relate to a physical entity as well as to physiological or environmental conditions wherein it would be possible that oviposition of the endoparasitoid to beads or capsules, serving as an artificial host for oviposition. A physical entity could be for instance a cage, a container, a green house comprising the beads or capsules and the endoparasitoid more or less closely together. Physiological or environmental conditions could for instance comprise the appropriate climate or climate regulation in term of temperature, light, humidity, etc, to establish optimal conditions for oviposition and optimal survival and rearing of eggs and larvae, other conditions such as the presence of wheat or cereal aphids, or other components providing odour or any other condition to mimic the natural environment of the endoparasitoid for oviposition.
According to another preferred embodiment said system comprises at one to several endoparasitoids chosen from the list of aphid endoparasitoids presented in Table 5.
The expression “at least one” as used herein relates to at least one in terms of numbers, such as “at least one organism or insect”. Alternatively the expression “at least one” can also mean “at least one species”, when for instance more than one kind of beneficial insect or endoparasitoid should be reared at the same time, and for each species one or more organism or insect can be contained within the system.
The invention, now being generally described, will be more readily understood by reference to the following tables, figures and examples, which are included merely for purposes of illustration of certain aspects and embodiments of the present invention and are not intended to limit the invention. All of the references mentioned herein are incorporated by reference.
The position of the needle is of importance as it needs be horizontal to produce good results.
Chitosan capsules are preferred to aphids (A). Presence of eggs in capsules after oviposition (C & D).
a) Description and Formation
1. Alginate Beads
Alginate occurs as the major structural polysaccharide of marine brown algae (Phaeophyceae). Chemically it is α (1→4)-linked linear block copolymer of β-D-mannuronic acid (M) and its C(5) epimer α-L-guluronic acid (G). The ratio M/G can strongly vary and is clearly correlate with the properties of alginates.
The formation of calcium alginate beads is the following. A solution containing 7,5 g/l of alginate (cecalgum: M/G=1,2) is dropped at room temperature through a needle to form droplets which fall into rapidly stirred 0,1 M solution of CaCl2. A bead (φ=2-3 mm) forms almost instantaneously due to the cross-linking of the alginate molecules by Ca++ cations.
2. Chitosan Beads
Chitosan, poly-β-(1-4)-2-amino-2-deoxy-D-glucopyranose, is a derivative of chitin, a polysaccharide found in a wide variety of crustacea, insects, and fungi.
The formation of chitosan beads is the following. Chitosan 10 g/l is dissolved in a solution of acetic acid 14 ml/l. The solution is dropped at room temperature through a needle to form droplets which fall into rapidly stirred pentasodium tripolyphosphate (pH 8,6). Droplets instantly form a chitosan polyphosphate beads (φ=2-3 mm). The beads are washed over to acetic acid and placed in pentasodium tripolyphosphate. After 30 minutes, beads are removed and rinsed with demineralized water
b) Acceptance by the Endoparasitoid.
Chemical cues perceived by the endoparasitoid through receptors in the antennae and tarsi are undoubtedly of great importance in host acceptance. Size, shape, colour and surface texture of the host is also very important. If accepted at this stage, they attempt to probe the host with their ovipositor. Nevertheless, parasitoids frequently insert their ovipositor into a host but do not go on to lay an egg. The ovipositor is normally covered in sensillae and it seems likely that the insect is rejecting the host after perceiving that it is unsuitable for oviposition. The parasitoid may assess the suitability of the host using chemical cues. Thus, we tested polymer beads as host for the endoparasitoid Aphidius rhopalosiphi. We determined influence of the colour (Table 1), the polymer type, alginate and chitosan, (Table 2) and the environment (Table 3) the presence of trehalose inside the capsule Table 7 and plant or host extract (Table 6) on the behaviour of the parasitoid.
1. Effect of Colour on Oviposition Behaviour
Our results show that response, attack and acceptance of parasitoids are better on the beads coloured in yellow than on the not coloured beads. Furthermore, we observe that the beads coloured with STABILOBOSS™ yellow (Art.Nr. 070/24, Germany) frequently cause the attack and the acceptance of the parasitoid in comparison with beads coloured with E102 (Vahine BP17, 84170 Monteux, France). Consequently, alginate beads coloured in yellow with the STABILOBOSS™ yellow marker, are preferred examples of hydrogel beads.
2. Effect of Biopolymer (Alginate or Chitosan) on Oviposition Behaviour
Our results show that response, attack and acceptance of the parasitoid are better on alginate beads that on chitosan beads. This is probably caused by the difference of colour between the beads. Indeed, alginate and chitosan differently absorb the colorant (Stabilo®). However, concerning the capsules, the opposite results were found. Chitosan is more attractive than alginate.
3. Effect of Environment on Oviposition Behaviour
In order to determine effect of environment on oviposition behaviour of the endoparasitoid Aphidius rhopalosiphi, we placed alginate beads coloured with the Stabilo® in different environment:
Results are displayed in table 3.
The results show that the near environment of the parasitoid may influence its oviposition behaviour. Indeed, when beads are placed with aphids or wheat, response of the parasitoid is more frequent. Furthermore, the percentage of parasitoid acceptance (acceptance/response *100) is important (19%) when the beads are placed with aphids and is very important (32%) when the beads are placed in a patch (aphids+wheat) in comparison with the reference (4%). Thus, it is possible that odours released by aphids and wheat excite the parasitoids.
4. Effect of the Presence of Trehalose Inside Chitosan Capsules.
Four kind of nutritive solution inside yellow chitosan capsules were compared with regards to the oviposition behavior and the number of eggs laid inside the said capsules by the parasitoids Aphidius rhopalosiphi.
It appeared that total number of attacked capsules, total number of capsules with eggs as well as the number of eggs collected in the capsules, and ratio between these two values are always higher in the case of Trehalose incorporated with dextran and secondly in trehalose incorporated by diffusion (Table 7). Yellow chitosan capsules containing trehalose are thus well suited for endoparasitoid oviposition. Eggs were found repeatedly in that kind of experiment.
5. Effect of Presence of Host Extracts on Oviposition Behaviour (See Table 7)
In order to determine the attractivity of epicuticular aphid compounds regarding endoparasitoids, epicuticular compounds were extracted from aphid exuviae using methanol. An exuviae is the cuticule remaining after the molting of the insect. This table shows the difference observed between oviposition behavior of Aphidius rhopalosiphi parasitoid on fresh exuviae (containing all epicuticular compounds), exuviae washed with methanol (Cold Meth) and exuviae re-applied with the methanol extract after washing. The behaviors measured are: of encounter (RENC), antennae contact (CA), abdomen fold (FOLD), ovipositor contact (CO), acceptance (FOLD+CO), and abdomen fold not follow by oviposition (FOLD Alone). It appeared that fresh exuviae as well as re-applied exuviae are more attractive than washed exuvia.
Further, an analysis is shown (Table 8) of the composition of the methanolic extract of epicuticular compounds belonging to the host that may be use to coat the beads or capsule in order to increase the level of oviposition in the beads or capsule. It was observed that this kind of extract with squalene increases the level of oviposition by the endoparasitoid in the bead or capsule.
Endoparasitoids often insert their ovipositor into the alginate beads coloured in yellow and placed in a “patch”. Nevertheless, it does always go on to lay an egg. Thus, it is possible that the beads are not a good support of laying for the parasitoids. Consequently, other supports were tested. Three kinds of biopolymer capsules: chitosan/dextran, chitosan/lambda-carrageenan and alginate/dextran were tested in the following.
a) Description and Formation
1. Chitosan/Dextran
Chitosan/dextran capsules are produced as follows. A solution containing 1% chitosan dissolved in water containing 1,4% (v/v) acetic acid is kept stirred using a magnetic stirrer at room temperature. An aqueous suspension containing 1,5% sodium polyphosphate and 40% dextran is extruded through a needle generating small droplets (φ=2-3 mm). Droplets instantly form a chitosan polyphosphate membrane enclosing the droplet. Capsules are removed from the solution and further treated in 1,5% sodium tripolyphosphate (pH 8,5) for half an hour. The capsules are rinsed and stocked in demineralized water.
2. Chitosan/Lambda-carrageenan
Chitosan/lambda-carrageenan capsules are produced as follows. A solution containing 1% chitosan dissolved in water containing 1,4% (v/v) acetic acid is kept stirred using a magnetic stirrer at room temperature. An aqueous suspension containing 1,5% sodium polyphosphate and 1,4% lambda-carrageenan is extruded through a needle generating small droplets (φ=2-3 mm). Droplets instantly form a chitosan polyphosphate membrane enclosing the droplet. Capsules are removed from the solution and further treated in 1,5% sodium tripolyphosphate (pH 8,5) for half an hour. The capsules are removed and washed over to acetic acid 1,4%.
The capsules are placed in pentasodium tripolyphosphate. After 30 minutes, capsules are rinsed with demineralized water and stocked in demineralized water.
3. Alginate/Dextran
Alginate/dextran capsules are produced as follows. A solution containing 0,5% sodium alginate is prepared and kept stirred using a magnetic stirrer at room temperature. An aqueous suspension containing 1,3% CaCl2 and 20% dextran is extruded through a needle generating small droplets (φ=2-4 mm) which fall into rapidly stirred alginate solution. A capsular membrane forms almost instantaneously around the suspension drop to the cross-linking of the interfacial alginate molecules by Ca++ cations. Prior to the removal of the capsules the polymer solution is diluted five-fold by adding required amount of milli-Q water. Finally, the capsules are removed and placed in a CaCl2 1,3% solution during 8 hours.
b) Acceptance by the Endoparasitoid.
Experiments showed that parasitoids laid eggs in the capsules of chitosan/dextran.
In order to optimise the shape, diameter, porosity and wall thickness of the biopolymer beads, the protocol of Somesh et al. 1988 was dramatically changed at several points. An overview of these changes is given in Table 9. Important differences are noted in italic.
TABLE 1
Alginate biopolymer beads as host for the endoparasitoid
Aphidius rhopalosiphi: influence of the bead colour.
Without colour
E102
STABILO ®
Response
1.6 ± 2.6
16.6 ± 8.2
13.5 ± 7.2
Attack
0.3 ± 0.8
3.6 ± 3.1
6.5 ± 4.2
Acceptance
0
1.7 ± 2.0
4.3 ± 3.5
Response is defined as the number of meetings with the bead of 30 parasitoid females observed during 15 minutes.
Attack is defined as the number of bends of the abdomen underneath the thorax orienting the ovipositor tip toward the bead of 30 parasitoid females observed during 15 minutes.
Acceptance is defined as the number of contact with the ovipositor of 30 parasitoid females observed during 15 minutes.
E102 (1:1H2O:E102) and Stabilo marker® (1:1H2O Stabilo) are used as yellow colorants.
TABLE 2
Beads as host for the endoparasitoid Aphidius rhopalosiphi:
influence of the biopolymer.
Response
Attack
Acceptance
Alginate
13.5 ± 7.2
6.5 ± 4.2
4.3 ± 3.5
Chitosan
10.6 ± 5.7
3.1 ± 2.6
1.4 ± 1.7
Response is defined as the number of meetings with the bead of 30 parasitoid females observed during 15 minutes.
Attack is defined as the number of bends of the abdomen underneath the thorax orienting the ovipositor tip toward the bead of 30 parasitoid females observed during 15 minutes.
Acceptance is defined as the number of contact with the ovipositor of 30 parasitoid females observed during 15 minutes.
TABLE 3
Alginate biopolymer beads as host for the endoparasitold
Aphidius rhopalosiphi: influence of the environment.
Response
Attack
Acceptance
Alone
12.4 ± 8.8
4.7 ± 5.0
0.5 ± 1.5
Aphids
20.1 ± 12.3
7.4 ± 7.7
3.9 ± 4.2
Wheat
25.2 ± 12.3
5.3 ± 5.3
1.3 ± 1.8
Aphids + Wheat
13.5 ± 7.2
6.5 ± 4.2
4.3 ± 3.5
Response is defined as the number of meetings with the bead of 30 parasitoid females observed during 15 minutes.
Attack is defined as the number of bends of the abdomen underneath the thorax orienting the ovipositor tip toward the bead of 30 parasitoid females observed during 15 minutes.
Acceptance is defined as the number of contact with the ovipositor of 30 parasitoid females observed during 15 minutes.
TABLE 4
Nutritive solution used to rear Aphidius rhopalosiphi larvae
basal medium
additives
SSM31
trehalose
600 mg/100 ml
vitamins
1 ml (stock)2
FBS (fetal bovine serum)
10% (v/v)
1SSM3 composition
Shields & Sang
1977
drosophila cell
Catalogue Number
S8398
mg/100 ml
b-alanine
25
alanine
150
arginine
50
asparagine
30
aspartic acid
30
cysteine
20
cystine
glutamic acid
1441
glutamine
60
glycine
50
histidine
55
hydroxyproline
isoleucine
25
leucine
40
lysine
85
methionine
25
phenylalanine
25
proline
40
serine
35
threonine
50
tryptophan
10
tyrosine
36
valine
40
TOTAL amino acids
2322
Sugar
glucose
1000
Vitamins
Choline
5
Mineral salts
Na2HPO4
88
MgSO4
215
CaCl2
76
BIS-TRIS buffer
105
oxalacetic acid
25
divers
yeast extract
100
pH
6.4
2Vitamins composition (mg/100 ml)
Biotin
0.008
Choline
90
Cyanocobalamine
0.05
folic acid
0.06
inositol
5
nicotinamide
1
pantothenic acid
0.8
pyridoxine
0.01
riboflavine
0.008
thiamine
0.008
TABLE 5
Relations between plants, greenflies and parasitoids
Greenfly
Host I
Host II
Parasitoïde
Acyrtosiphon caraganae
Aphidius ervi (Hal.)
Toxares deltiger (Hal.)
Acyrtosiphon kindoi
Aphidius eadyi
Praon volucre (Hal.)
Acyrtosiphon pisum (Harr.)
Urtica dioicaL.
Aphidius eadyi
Family of legumes: Vicia faba
Aphidius ervi (Halyday)
L., pea, bean, clover
Aphidius picipes
Aphidius smithi
Aphidius urticae
Praon dorsale
Praon volucre (Halyday)
Toxares deltiger (Hal.)
Aphis fabae (Scop.)
Evonymus europaea
Aphidius colemani (Vier.)
Aphidius matriarcae (Hal.)
Ephedrus plagiator (Nees)
Lipolexis gracilis (Förster)
Lysiphlebus cardui
Lysiphlebus fabarum (Marshall)
Praon abjectum (Hal.)
Praon volucre (Hal.)
Trioxys angelicae (Haliday)
Brachycaudus helichrysi
Prunus spinosa
Asteraceae
Brachycaudus sp.
Dysaphis sp.
Ephedrus persicae (Frog.)
Ephedrus plagiator (Nees)
Lipolexis gracilis (Förster)
Lysiphlebus fabarum (Marshall)
Paralipsis enervis (Nees)
Praon volucre (Hal.)
Trioxys angelicae (Halyday)
Cinara sp.
Pauesia sp.
Diuraphis noxia
Diaretiella rapae (M'Intosh)
(Kurdjumov)
Drepanisiphum platanoidis
Acer spp.
Aphelinus thomsoni (Graham)
Elatobium abietinum
Picea
Forda sp.
Monoctonia pistaciaccola
Hyalopterus pruni (Geoffr.)
Prunus
Phragmites communis
Ephedrus plagiator (Nees)
Praon volucre (Halyday)
Macrosiphon pisum
Family of legumes
Aphidius ervi (Hal.)
Macrosiphum euphorbiae
Rosa spp.
Solanaceae
Aphidius ervi (Hal.)
Aphidius nigripes
Metopolophium dirhodum
Rosa spp.
Grasses
Aphelinus abdominalis
Aphidius ervi (Hal.)
Aphidius picipes
Aphidius rhopalosiphi
Aphidius ukbekistanicus
Ephedrus plagiator (Nees)
Praon volucre (Hal.)
Toxares deltiger (Hal.)
Metopolophium fetuscae
Aphidius ervi (Hal)
(Theobald)
Aphidius picipes
Aphidius rhopalosiphi
Aphidius uzbekistanicus
Microlophium carnosum
Urtica dioica
Aphidius ervi (Hal.)
(Buckton)
Aphidius picipes (Nees)
Aphidius urticae
Microlophium evansi
Urtica dioica L.
Aphidius ervi (Hal.)
Mindarus abietinus (Koch)
Pseudopraon minderphagum
Myzus persicae
Prunus persicae
Potato
Aphidius colemani
Turnip
Aphidius ervi (Hal.)
Chrysanthenum
Aphidius matricariae
Brassicacae (cultivars)
Diaretiella rapae (M'Intosh)
Ephedrus cerasicola
Ephedrus plagiator (Nees)
Ononis spp.
Urtica dioica L.
Pemphigus sp.
Monoctonia pistaciaecola
Periphyllus acericola
Acer pseudoplatanus
Praon sylvestre (Stary)
(Walker)
Trioxys flacatis (Alaekauer)
Periphyllus aceris
Acer platanoides
Praon sylvestre (Stary)
(Linnaeus)
Trioxys flacatis (Alaekauer)
Periphyllus coracinus
Acer platanoides
Aphidius setiger
(Koch)
Trioxys glacatus (Alaekauer)
Periphyllus hirticornis
Acer campestre
Aphidius setiger
(Walker)
Praon sylvestre (Stary)
Trioxys flacatus (Alaekauer)
Periphyllus lyropictres
Acer platanoides
Aphidius setiger
(Kessler)
Acer pseudoplatanus
Trioxys flacatus (Alaekauer)
Periphyllus obscurus
Acer campestre
Trioxys flacatus (Alaekauer)
(Mamontova)
Periphyllus sp.
Acer spp.
Praon sylvestre
Periphyllus testudinaceus
Acer campestre
Praon sylvestre (Stary)
(Fernie)
Acer platanoides
Trioxys flacatus (Alaekauer)
Acer pseudoplatanus
Protolachnus sp.
Diaretus leucopterus (Hal.)
Rhopalosiphum padi
Prunus padus L.
Crops
Diaretiella rapae (M'Intosh)
Capsella bursa-pastoris
Trioxys angelicae (Halyday)
Schizolachnus sp.
Pauesia unlilachni (Gahan)
Schizophis graminum
Sorgho
Aphidius rhopalosiphi
(Rondoni)
Orge
Lysiphlebus testaceipes (Cresson)
Sitobion avenae
Grasses
Aphidius avenaphis (Fitch)
Aphidius ervi (Hal.)
Aphidius picipes (Nees)
Aphidius rhopalosiphi
Aphidius uzbekistanicus
Diaretiella rapae (M'Intosh)
Ephedrus plagiator (Nees)
Praon volucre (Hal.)
Toxares deltiger (Hal.)
Sitobion fragariae
Rubus fructicosus
Grasses: Avena sativa L.
Aphidius ervi (Hal.)
Digitalis sp.
Aphidius rhopalosiphi
TABLE 6
Consequence of Trehalose presence on the oviposition
behaviuor of Aphidius rhopalosiphi.
Parametres
T
ThDex
ThDiff
JP
Total nb of capsules
60
60
60
60
% attacked capsules
23.33%
46.67%
46.67%
36.67%
Nb of attacks per attacked
2.57
5.04
11.43
4.86
capsules
Nb of capsules with eggs
0
6
1
0
% of capsules with eggs/total
—
10%
1.67%
—
capsules
% of capsules with eggs/total
—
21.42%
3.57%
—
attacked capsules
Total number of eggs found
0
10
2
0
inside the capsules
% eggs/total capsules
—
16.67%
3.33%
—
% eggs/total attacked capsules
—
35.71%
7.14%
—
T: Control capsule: Chitosan capsule + yellow stabilo
ThDex: yellow capsules + trehalose mixed with dextran.
ThDiff: yellow capsules + trehalose introduced by diffusion.
JP: yellow capsules containing extracts of grinded aphids.
TABLE 7
Attractivity of epicuticular aphid compounds
regarding endoparasitoids
Behavior
Fresh
REAPP
Cold METH
RENC
31.0
40.2
15.2
CA
21.7
16.6
5.5
FOLD
3.7
2.2
0.8
CO
8.5
2.7
1.7
ACCEPT
12.1
4.9
2.5
FOLD Alone
3.7
2.2
0.8
TABLE 8
Composition of the methanolic extract. Squalene was also present.
Identified molecules
retention time (min)
methyle tetradecanoate
9.98
methyl 9-methyl tetradecanoate
11.32
methyl cis-9-octadecanoate
12.45
methyl hexadecanoate
12.73
methyl cis,cis-9-12-octadienoate
Near the following peak
methyl cis-9-octadecenoate
15.28
methyl octadecanoate
15.59
TABLE 9
Modification to protocol for preparation of chitosin capsules for oviposition.
Somesh et al. 1988:
Techniques for preparing
hydrogel membrane capsules
Invention
Polymer Solution
1% (w/v) of Chitosan (Sigma)
0.75% (w/v) of Chitosan
1.4% (v/v) acetique acid.
<<medium >>
1.4% (v/v) acetique acid
Ionic Solution
1.5% (w/v) pentasodium-tri-
2.5% (w/v) pentasodium tri-
polyphosphate
polyphosphate
40% (w/v) Dextran (Sigma).
20% (w/v) Dextran (Sigma)
Duration in chitosan
No data
5 min (essential to control the thickness
of the walls)
Rinsing of capsules
acetique acid 1.4% (v/v)
acetique acid 1.4% (v/v)
Maturation time
30 min in pentasodium-tri-
15 min in pentasodium tri-
polyphosphate 1.5%
polyphosphate 2.5% (w/v)
Agitation of polymer
No data
600 rpm
solution
Diameter of the
Not given
0.45 mm
needle
Delivery rate of ionic
Not given
7 ml/min (ou 100 droppletss/min)
solution
pH
Not given
pH of polymer solution: 3.5
(obligatory t < 5.5)
pH of ionic solution: range between
6 to 9
Characteristics favouring the oviposition in the capsules
Capsules color
No object
Stabilobloss at 4%
Capsules content
No object
Trehalose
Hance, Thierry, Debatty-Mestdagh, Michèle, Cambier, Vincent, Boegen, Catherine, Muratori, Frédéric, Lebbe, Olivier, Dos Santos Goncalves, Ana-Maria
| Patent | Priority | Assignee | Title |
| 8647686, | Aug 30 2007 | The United States of America, as represented by The Secretary of Agriculture | Insect diet formulations and methods for rearing insects |
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